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Antimicrobial Resistance and Plasmid Profiles of Campylobacter Species from Infants Presenting with Diarrhoea in Osun State, Nigeria | OMICS International
ISSN: 2161-0703
Journal of Medical Microbiology & Diagnosis

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Antimicrobial Resistance and Plasmid Profiles of Campylobacter Species from Infants Presenting with Diarrhoea in Osun State, Nigeria

Adekunle OC1* and Onilude AA2

1Department of Medical Microbiology and Parasitology, Ladoke Akintola University of Technology, Ogbomoso, Nigeria

2Department of Microbiology, University of Ibadan, Ibadan, Nigeria

*Corresponding Author:
Adekunle OC
Department of Medical Microbiology and Parasitology
Ladoke Akintola University of Technology
Ogbomoso, Nigeria
Tel: 2348067624952
E-mail: [email protected]

Received date: September 22, 2014; Accepted date: December 11, 2014; Published date: December 13, 2014

Citation: Adekunle OC, Onilude AA (2015) Antimicrobial Resistance and Plasmid Profiles of Campylobacter Species from Infants Presenting with Diarrhoea in Osun State, Nigeria. J Med Microb Diagn 4:172. doi:10.4172/2161-0703.1000172

Copyright: © 2015 Adekunle OC, et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.

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Antibiotic resistance among enteric bacterial pathogens complicates the heavy diarrhoea disease burden. Antimicrobial resistance of Campylobacter spp. to fluoroquinolones, which are generally used for the treatment of bacterial gastroenteritis, has increased during the past two decades, mainly as a result of the approval of this group of antimicrobials for use in food- producing animals. Twenty five Campylobacter isolates gotten from humans were subjected to antibiotics testing using Kirby Bauer disc diffusion method as well as standard E-test method. The plasmid profile of the isolates was determined using the Alkaline phosphatise procedure. The antimicrobial susceptibility testing of these isolates showed that all were sensitive to Erythromycin and Ciprofloxacin while none was sensitive to co-trimoxazole. The standard organisms were sensitive to co-trimoxazole (80%) and ciprofloxacin (65%) but were resistant to erythromycin (70%). No plasmid was found in streptomycin and ampicillin resistant strains, with the exception of four isolates which were co-trimoxazole-resistant and which contained around 24.4kb plasmids.


Campylobacter; Antibiotics; Plasmids


The most common human disease caused by Campylobacters is acute gastroenteritis [1]. A collective name for infectious disease caused by members of these bacteria is called Campylobacteriosis [2]. Campylobacter infections are among the most common bacterial infection in humans. It is characterized by profuse, often bloody diarrhoea, particularly in children, acute abdominal pain and fever. They produce both diarrheal and systemic illness. Most cases recover after a period of bed rest like other enteric infections. It is usually cleared up on their own but sometimes is treated with electrolyte replacement and rehydration therapy. Antimicrobial treatment (erythromycin, tetracycline or fluoroquinolone) can be used in invasive cases to eliminate the carrier state. It can also shorten the duration of symptoms if given early in the illness [3]. Most clinical isolates of C. jejuni were reported to be resistant to ciprofloxacin and azithromycin.

However, antimicrobial resistance to clinically important drugs used for treatment (especially macrolides and fluoroquinolones) is increasingly reported for Campylobacters. There is evidence that patients infected with antibiotic-resistant strains suffer worse outcomes (invasive illness or death) than those infected with sensitive strains [4]. Antibiotic susceptibility studies are necessary because variation occurs from country to country and from place to place. Studies in Europe have shown C. jejuni to be sensitive in-vitro to antibiotics such as tetracycline, erythromycin and gentamycin while many strains are resistant to ampicillin, pencillin and metronidazole [5]. The development of antimicrobial resistance in the last four decades has led to an intensification of discussion about the prudent use of antimicrobial agents, especially in veterinary medicine, since their use and the development of resistance in human and animals are interrelated [6]. There is an increased rate of resistance to erythromycin, which is the drug of choice for the treatment of campylobacter enteritis. The resistance to erythromycin by these strains might be due to the presence of plasmid harboured by these organisms. In this study, we present the occurrence of drug resistance among 25 strains of Campylobacter species isolated from children with diarrhoea. The frequency of plasmid as well as the relationship between antibiotic resistance and plasmid carriage was also investigated.

Materials and Methods

Stool samples were obtained from children with incipient diarrhoea between ages one month and 36 months. Faecal samples were cultured on Butzler- type medium which consisted of Butzler agar; 5% sheep blood; CAT from Oxoid comprised of cefoperazone, vancomycin and amphotericin B as selective agents. The incubation was done at 42°C for 72hr in a microaerophilic atmosphere using CO2 incubator (Sanyo CO2 incubator Model MCO-15A, Japan). The incubation was done in an atmosphere with reduced oxygen (5%) with added carbon-dioxide (10%) and 85% N2. The isolated strains were identified according to established criteria for Campylobacter species using biochemical tests [7].

Antibiotic Sensitivity Testing of Isolates

The antibiotics used included ampicillin (25 μg), streptomycin (10 μg), ciprofloxacin (5 μg), nalidixic acid (30 μg), erythromycin (10 μg), tetracycline (10 μg), gentamycin (10 μg), co-trimoxazole (25 μg), nitrofurantoin (200 μg), ceftriazole (30 μg) from Oxoid. The Kirby Bauer disc diffusion method for in vitro susceptibility testing was employed in this study. Media plates containing different colonies were inoculated and incubated. The inoculum compared with 0.5 Macfarland standards and Mueller-Hinton agar was used. The zones of inhibition of the test strains when comparable with the zone of inhibition of control organism were interpreted as sensitive, while those showing no zones of inhibition or narrower zones of inhibition than those of sensitive control organisms were interpreted as resistant. The antimicrobial susceptibility testing was also performed by using the standard E-test method. The bacterial inoculum was adjusted to 0.5 Macfarlane standard turbidity using the Mueller Hinton agar. All plates were incubated at 37oC for 48 hours under microaerophilic conditions. Results were interpreted according to the Clinical Laboratory Standard Institute (CLSI) guidelines (CLSI document M 45-A and M 100-S17, clinical, 2006, 2007), using the following resistance break point of C.jejuni/coli:ampicilin, >16 mg/L,Ciprofloxacin>4 mg/L, gentamicin >16 mg/L, erythromycin > 32 mg/L nalidixic acid >32 mg /L, and streptomycin >16 mg/L. The following reference strains were used as controls: C. jejuni subsp jejuni ATCC 2q428™ and Campylobacter coli ATCCR 33559™ purchased from ATCC.

Plasmid Isolation

Isolation of Plamids was done by Birnobiom and Doly Method (1984). Electrophoretic gels electrophresis was prepared by dissolving and boiling 1.0 g agarose in 100ml 1X TBE buffer solution. The gel was allowed to cool to about 45oC and 10 ul of 5 mg/ml ethidium bromide was added, mixed together before pouring it into an electrophoresis chamber set with the combs inserted. After the gel has solidified, 10 ul of the plasmids DNA and 2 ul of 6X loading dye was mixed together and loaded in the well created. Electrophoresis was carried out at 80V for 1hour. The plasmid was visualized and photographed on UV light source. Supercoiled DNA ladder (2-16kb) (Life Technologies, Brazil) and plasmids of known molecular mass of Campylobacter coli (49, 3.9 and 3.4 kb) [8] were used to determine the approximate molecular mass of each plasmid. Those that carry plasmids were cured by treatment with sodium lauryl sulphate (SDS).

Statistical analysis

Statistical analysis of obtained empirical results was done using Minitab 11.


Twenty five Campylobacter isolates were obtained from stool samples. All isolates were sensitive to erythromycin and ciprofloxacin but none was sensitive to co-trimoxazole (Table 1). In the antibiotic susceptibility pattern of Campylobacter isolates in Table 1 Ciprofloxacin and Erythromycin were one hundred percent effective, followed reducingly by Cefriazole (84%), Gentamycin and Nalidixic acid (82% and 80% respectively) Co-trimozale was totally ineffective against the Campylobacter isolates. The best minimum inhibitory concentration which is the lowest concentration of drug that inhibits the growth of Campylobacter species was observed using 0.025 μg/ml of ciprofloxacin.

  SS RS  Total
Ampicillin 25µg 13(52)* 12(48)*5
Streptomycin 10µg 12(48) 13(52) 25
Ciprofloxacin 5µg 25(100) 0(0)     25
Nalidixic acid 30µg 20(80) 5(20)   25
Erythromycin 10µg 25(100) 0(0)    25
Tetracyline 30µg 18(72) 7(28)  25
Gentamycin 10µg 20(82) 5(20)  25
Cotrimoazole 25µg 0(0) 25(100)2
Nitrofurantoin 200µg 18(72) 7(28)  25
Ceftriaxone 30µg 21(84) 4(16) 25

Table 1: Frequency of Antibiotics susceptibility among of the Campylobacter isolates obtained from stool samples of infants presenting with diarrhoea-like symptoms.


The antimicrobial susceptibility testing of these isolates showed that (100%) were sensitive to Erythromycin and Ciprofloxacin. This conforms to the study by [9] which has shown that Erythromycin and ciprofloxacin as the drugs of choice for the treatment of Campylobacterrelated diarrhea [9]. People having diarrheoa showed high resistance to antibiotics like ampicillin, streptomycin, tetracycline and total resistance to co-trimoxazole. They are widely used in Nigeria even when they were not prescribed. Resistance to these drugs is common in this part of the world because there are no guidelines and controlled access to drugs, situation that can lead to development of resistance even where there are guidelines, the regulatory agencies are inefficient. The use of these drugs for infections other than gastroenteritis along with self-medication is often the causes of resistance in developing countries. In developed countries, resistance is due to their use in food animals and travel to developing countries. The increase in erythromycin resistance in developed countries is often low and stable at approximately 1% to 2% which is the reverse for developing countries [10]. For example, in 1984, 82% of Campylobacter strains from Lagos, Nigeria, were reported sensitive to erythromycin which 10 years later came down to only 20.8% were sensitive [2]. In addition, resistance to another macrolide, azithromycin, was observed in 7% to 15% of Campylobacter isolates in 1994 and 1995 in Thailand [11]. Antibiotic susceptibility profile of microorganisms vary from country to country, province to province, town to town, and hospital to hospital in the same town as well as between private and public healthcare facilities in the same area. In addition, different pathologies may alter antibiotic sensitivity patterns. Consequently, periodic evaluation of antibiotic susceptibility is recommended to guide management of patients requiring antibiotic treatment. Results of plasmid analysis to determine presence of extra chromosomal genes that may confer resistance on the organisms showed four (4) isolates presenting with plasmids. There is the possibility of the other isolates losing their plasmids during the tests. No plasmids were found in streptomycinresistant and ampicillin-resistant strains, with the exception of four isolates which contained a 24.4 Kb plasmid and were co-trimoxazoleresistant.

Furthermore, plasmid analysis of the isolates showed that some of them possess extra chromosomal gene of about 24.4 kb that could have conferred multi-resistance on them. However, when the four organisms containing plasmids were treated, they became sensitive to the antibiotics earlier resistant to.


The Authors thank Prof.A.A. Onagbesan and all the staff of Biotechnology Department, Federal University of Agriculture, Abeokuta for their contributions towards the success of the work.


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